Self-Referencing Sensor for Chemical Detection

ABSTRACT

Provided herein is a sensing apparatus comprising, at least one LSPR light source, at least one detector, and at least one sensor for LSPR detection of a target chemical. The sensor comprises a substantially transparent, porous membrane having nanoparticles immobilized on the surface of its pores, the nanoparticles being functionalized with one or more capture molecules. There is further provided a self-referencing sensor for distinguishing non-specific signals from analyte binding signals. The self-referencing sensor comprising one or more nanoparticles having at least two distinct LSPR signals.

CROSS REFERENCE TO PRIOR APPLICATIONS

The present application is a Continuation of U.S. patent applicationSer. No. 17/063,424 filed Oct. 5, 2020, which is a Continuation of U.S.patent application Ser. No. 15/134,843 filed Apr. 21, 2016, which is aContinuation-in-Part of U.S. patent application Ser. No. 14/216,042filed Mar. 17, 2014, which claims priority under Paris Convention toU.S. Application No. 61/798,450, filed Mar. 15, 2013, the entirecontents of which are incorporated herein by reference.

TECHNICAL FIELD

The following relates generally to a method and apparatus for chemicaldetection. More particularly it relates to a self-referencing sensor andan apparatus comprising the sensor.

BACKGROUND

Determining the presence and concentration of bio-molecules and otherchemicals in a fluid is important in many applications. For example, aninstrument that can determine the concentration of one or more specificchemical targets in a gas or liquid containing various chemicals mayhave applications in medical diagnostics, high throughput drugdevelopment, environmental testing, defense and laboratory-basedresearch. Such techniques are also important for biomolecularinteraction analysis in which reaction kinetics (on and off rates),affinity, and specificity are determined, along with other importantparameters.

A common strategy to detect a chemical target is to use an instrumentwith a capture molecule which binds to the target chemical of interestand a transducer that allows the user to observe the binding event.Preferably, the capture molecule preferentially or exclusively binds tothe chemical target. In the case of bio-molecular targets, antibodies,aptamers and polymers are used as capture molecules.

Optical transduction of binding events is a common detection method. Tooptically observe a binding event between a capture molecule and atarget, various spectrometric techniques can be employed. Thesetechniques may require that capture molecules be labeled with atransducer or tag, such as a fluorescent molecule for fluorescencespectroscopy or a Raman tag for Raman spectroscopy. A technique used formedical diagnostics is enzyme linked immunosorbant assay (ELISA) thatutilizes fluorescently-labeled antibodies to detect various targetchemicals, including bio-molecules, in human biological fluids to detectdisease.

Labeled assays may be disadvantageous because labeled capture moleculesmay have adverse effects on assay results due to steric hindrances.Assays comprising labeled capture molecules are also not compatible withreal-time testing. Labeling capture molecules also increases devicecomplexity and cost.

Label-free assays, which do not require the addition of a labeledcapture molecule, are advantageous because the target chemical is notsterically hindered from binding to the capture molecule by a label.Label-free assays may also measure binding events in real time, whichimproves the performance and sensitivity of the assay. Label-free assayscan also be used for biomolecular interaction analysis as they providereal time data.

Metal nanoparticles, between 1 nm and 1000 nm in various dimensions, maybe used as transducers in diagnostic assays. Some nanoparticle baseddiagnostic assays are ‘label-free’. Metal nanoparticle transducers canbe used to monitor binding events in real time without additional labelsthrough a phenomenon known as localized surface plasmon resonance(LSPR).

LSPR is a phenomenon associated with noble metal nanoparticles thatcreates sharp spectral absorbance and scattering peaks and producesstrong electromagnetic near-field enhancements. These spectral peaks canbe monitored using absorbance spectroscopy. The spectral peak changeswith refractive index changes in the immediate vicinity of thenanoparticle surface. When chemical targets are bound near the surfaceof a metal nanoparticle, a shift in the spectral peak occurs due tochanges in the local refractive index. This can be used to determine theconcentration of a specific target in a complex medium.

LSPR sensors operate through the immobilization of metal nanoparticlesonto a flat surface. The nanoparticles are functionalized with specificcapture molecules, which may be an antibody. The sample fluid ofinterest is flowed over the top of the metal nanoparticles, the targetchemicals of interest bind to their respective capture molecules, andthe overall spectral peak of the sensor shifts according to theconcentration of the chemical target on the capture molecules. In orderto measure this shift, reflectance or transmission absorbancespectroscopy may be employed. Quantification is possible throughcomparing results to a previously-developed standard curve.

However, LSPR sensors suffer from low sensitivity and inadequatedetection limits for a number of reasons.

LSPR sensors with nanoparticles on planar surfaces operate by flowingthe sample longitudinally over the surface. In order for the sensor todetermine the target concentration with the highest sensitivity andaccuracy, the sensor must reach chemical equilibrium. Equilibrium occurswhen the maximum fraction of capture molecule binding sites are occupiedby chemical targets on the sensor surface, resulting in the largestsensor response in a reaction-limited assay. Lengthy incubation timesare required to reach equilibrium.

Long incubation times are not suitable for many applications includingpoint-of-care diagnostics. Long incubation times may be problematic fortypes of planar sensors other than LSPR sensors.

Reflectance LSPR signals from nanoparticles on a planar surface are alsoweak, leading to poor signal to noise ratios and poor detection limits.This may be addressed by using nanostructured surfaces to increase thesurface area and nanoparticle density, resulting in a larger LSPRsignal. However, this has the negative effect of increasing the time ittakes to reach equilibrium and obtain the highest fraction of surfacecoverage since the number of surface sites is greatly increased.Essentially this improves signal to noise ratio but worsens the time toreach equilibrium, and overall does not greatly improve sensorperformance. Moreover, these techniques rely on reflection measurementsystems because the materials used are opaque at LSPR wavelengths andwill not allow for transmission measurements.

For typical surface plasmon resonance (SPR) and localized surfaceplasmon resonance (LSPR) based devices used for the quantification ofmolecular binding interactions, a reference channel may be used tosubtract interfering nonspecific signals to produce a more accuratebinding measurement. Sources of these nonspecific signals include butare not limited to, nonspecific binding interactions of target ornon-target molecules with the sensor, solution phase bulk refractiveindex changes, as well as fluctuations in temperature or otherexperimental conditions. If these interfering signals can be quantified,they can be subtracted out from the sensing signal to obtain a moreaccurate response of the desired signal. The testing channel and testingsensor contain capture molecules on the sensor surface that bindspecifically to the analyte of interest. To prevent the referencechannel sensor from binding to the analyte of interest, the surface maybe blocked with a neutral molecule. In this manner, all nonspecificchanges such as those listed above will affect both sensors but thespecific binding interaction will only affect the tested sensor. Thedifference in signal between the two sensors can then be used tosubtract the non-specific effects from the effect of the analyte ofinterest.

The reference channel typically runs parallel or serial to the testingchannel and is composed of a redundant sensor that may require separatelight sources, detectors and microfluidics to be effective. Its presenceincreases the cost of the instrument, makes it more complicated and mayrequire larger amounts of precious sample to operate. For the referencechannel to perform correctly everything about it must be identical tothe tested sensor. Since the reference channel requires a separatesensor and surface functionality than that of the testing channel, it isnear impossible to produce a perfectly accurate reference signal. Italso requires that the user design and produce a reference surfacecoating that is appropriate, adding to the experimental complexity.

LSPR-based molecular sensing using nanoparticles may also be carried outin solution phase, i.e. free floating nanoparticles not immobilized ontoa substrate. Detection in solution phase is typically achieved by addingthe analyte of interest to the solution of nanoparticles functionalizedwith capture molecules. This detection signal would normally include thenonspecific effect of the dilution of the nanoparticle solution alongwith any bulk refractive index shifts provided by the analyte and itsbuffer. These non-specific effects currently cannot be quantifiedwithout running additional control experiments, increasing the amount ofsample to be used, time needed and complexity of the experiments.Similar to substrate-based SPR/LSPR sensing, it is near impossible toproduce a perfectly accurate reference signal using this method.

SUMMARY

In one aspect, there is provided a sensor for LSPR detection of a targetchemical. The sensor comprises a substantially transparent, porousmembrane having nanoparticles such as metal nanoparticles immobilized onthe surface of its pores, the nanoparticles being functionalized withone or more capture molecules.

In a further aspect there is provided an sensing apparatus comprising atleast one LSPR light source; at least one detector and at least onesensor for LSPR detection of a target chemical located between thedetector and the light source, the sensor comprising a substantiallytransparent, porous membrane, the membrane comprising nanoparticlesimmobilized on the surface of its pores, the nanoparticles beingfunctionalized with one or more capture molecules.

In a further aspect of the invention there is provided aself-referencing sensor for LSPR detection of an analyte molecule in asample and simultaneous detection of non-specific signal changes, theself-referencing sensor comprising one or more types of nanoparticles,the one or more types of nanoparticles having at least two distinct LSPRsignals, wherein at least one nanoparticle type includes a capturemolecule to bind to the analyte and whereby the non-specific signalchanges can be distinguished from the analyte binding signal by adifference in a resulting optical spectrum change between the twodistinct LSPR signals.

BRIEF DESCRIPTION OF THE DRAWINGS

Embodiments will now be described by way of example only with referenceto the appended drawings wherein:

FIG. 1 is a diagram of a transmission-based three-dimensional chemicalsensing system;

FIG. 2 is a side view of the fluidic cartridge of FIG. 1 ;

FIG. 3 is a top view of a fluidic cartridge of the chemical sensor ofFIG. 1 ;

FIG. 4A is graphical representation of an enlarged top view of a sensorof FIG. 3 ;

FIG. 4B is an enlarged view of the graphical representation of thesensor of FIG. 4A depicting functionalized nanoparticles immobilized inpores;

FIG. 4C is an enlarged side view of a pore of FIG. 4A depictingfunctionalized metal nanoparticles;

FIG. 4D is another enlarged view of a pore depicting various types offunctionalized metal nanoparticles immobilized the pore;

FIG. 5 is an process flow diagram outlining an example for obtaining areading from the chemical-sensing system of FIG. 1 ;

FIG. 6 is a plot showing the resonance peak shift due to binding of thetarget chemical with capture molecules on a sensor;

FIG. 7 is an overhead view of a fluidic cartridge similar to that ofFIG. 3 comprising multiple sensors;

FIG. 8 is scanning electron microscope (SEM) image of 20 nm goldnanoparticles immobilized on an anodized aluminum oxide (AAO) membranewith a 200 nm pore diameter;

FIG. 9A is a photograph of gold nanoparticles(GNP) immobilized on aglass slide;

FIG. 9B is a photograph of gold nanoparticles immobilized on an AAOmembrane;

FIG. 10 is an example plot showing the relationship between absorbanceand wavelength for an AAO membrane having gold nanoparticles immobilizedin its pores with respect to a glass slide having gold nanoparticlesimmobilized on its surface;

FIG. 11 is an example plot showing resonance peak shift with respect totarget concentration in a solution;

FIG. 12 is a process flow diagram of an example process for GNPimmobilization on the pores of an AAO substrate and subsequentfunctionalization with capture molecules and blocking molecules;

FIG. 13 is an image of AAO membrane with gold nanoparticles immobilizedthereon without the use of BSA additive or coating;

FIG. 14 is a photograph of a clean AAO membrane;

FIG. 15 is a diagram showing an example method to enhance the LSPR shiftfor small molecule targets.

FIG. 16 is a graph showing a comparison of reflection and transmissionsignal of AAO membrane with 150 nm pores and 50 um thick, with 45 nmgold shell nanoparticles immobilized inside the pores. The LSPR peak ismuch larger and sharper in the transmission measurement.

FIG. 17 is graph showing transmission of AAO membranes of various poresize (P, in nm) and thickness (T, in um). Membranes were measured dry inair.

FIG. 18 is a graph transmission of AAO membranes of various pore size(P, in nm) and thickness (T, in um). Membranes were measured wetted withwater in air.

FIG. 19 is an absorbance spectrum of an AAO membrane containingnanoparticles with two different LSPR peak positions, one located atapproximately 495 nm and the other at approximately 580 nm.

FIG. 20 shows the response of the T3D sensor to serial injections of thestreptavidin (SA) protein, from 0.5 nM to 20 nM. The streptavidin bindsto the biotinylated surface of the nanoparticles inside the AAOmembrane.

FIG. 21 shows the response of the conventional 2D sensor to serialinjections of the streptavidin (SA) protein, from 5 nM to 80 nM. Thestreptavidin binds to the biotinylated surface of the nanoparticleswhich are immobilized onto a glass surface.

FIG. 22 shows that BSA prevents nanoparticles from binding to a PAHtreated surface, on a glass slide.

FIG. 23 is a schematic depicting a self-referencing sensor comprisingnanoparticles in solution functionalized with capture molecules andblocking molecules.

FIG. 24 . Is a schematic depicting a self-referencing sensor comprisingnanoparticles on a substrate surface containing one particle typefunctionalized with capture molecules and a second particle typefunctionalized with only blocking molecules.

FIG. 25A is a cross-section top view of a self-referencing sensorapparatus setup; FIG. 25B is a schematic depicting more than onenanoparticle type with different functionalization on the same substratewhich may be interfaced with a fluidic channel between the LSPR lightsource and the detector.

FIG. 26A is a cross-section top view of a self-referencing sensorapparatus. FIG. 26B is a schematic depicting one nanoparticle type onone substrate. FIG. 26C is a schematic depicting another nanoparticletype on another substrate. Both substrates may interface with the samefluidic channel in the same optical path between the LSPR light sourceand the detector in the apparatus as shown in FIG. 26 a.

FIG. 27 is a graph showing the absorbance spectrum of a sensorcontaining a single particle type immobilized onto the substrate, whichproduces two distinct LSPR peaks.

FIG. 28A is a photograph of a self-referencing sensor containing twotypes of nanoparticles immobilized within the same area on a glasssubstrate. FIG. 28B is a graph showing the absorbance spectrum of thesensor of FIG. 28A containing two distinct LSPR peaks.

FIG. 29 is a series of graphs showing the resonance peak shifts observedwith a self-referencing sensor with (top) detection of bulk effects,(middle) detection of specific molecule only, and (bottom) detection ofspecific molecule with bulk effects using a combination of twonanoparticle types, one functionalized with capture molecules and theother with blocking molecules.

FIG. 30 is a series of graphs showing experimental results of resonantpeak shifts observed when tracking both functionalized and blockedparticles of a two nanoparticle type self-referencing sensor.

FIG. 31 is a graph showing experimental results demonstrating theability to correct a specific binding curve that has been convolutedwith bulk effects with a self-referencing sensor.

FIG. 32A and FIG. 32B are graphs showing experimental results of a twonanoparticle type self-referencing sensor system, with both particletypes containing the same functionalization. FIG. 32A shows measuredchanges over time, of LSPR peak positions with addition of bulkrefractive index changes (a) and a binding molecule (b). FIG. 32B showsthe processed separated signals corresponding to specific binding andbulk refractive index changes.

FIG. 33A and FIG. 33B are graphs showing experimental results of asingle nanoparticle type self-referencing sensor system, producing twodistinct LSPR peaks. FIG. 33A shows measured changes in LSPR peakposition with addition of bulk refractive index changes (a) and abinding molecule (b). FIG. 33B shows the processed separated signalscorresponding to specific binding and bulk refractive index changes.

FIG. 34A is a graph of an absorbance spectrum showing two LSPR peaks ofa two nanoparticle type self referencing sensor. FIG. 34B are graphsshowing the self-referencing sensor response over time for thefunctionalized and blocked particles.

FIG. 35A are graphs showing the raw signals obtained from functionalizedparticles and blocked particles upon exposure to analyte with bulkbackground. FIG. 35B is a graph showing the corrected binding responseswith the bulk background removed.

FIG. 36A is a photograph of a self-referencing sensor comprising twonanoparticle types immobilized onto the same area of a glass substrate.FIG. 36B is the absorbance spectrum of the self-referencing sensor. FIG.36C are graphs showing the LSPR sensor response over time for both thefunctionalized and blocked nanoparticles.

FIG. 37A is a photograph of a self-referencing sensor comprising twonanoparticle types present in solution. FIG. 37B is the absorbancespectrum of the self-referencing sensor. FIG. 37C are graphs showing theLSPR sensor response over time for both the functionalized and blockednanoparticles.

DETAILED DESCRIPTION

It has now been realized that the long incubation times associated withexisting LSPR sensors are due, at least in part, to the diffusion timerequired for target chemicals in a fluid to reach capture molecules onthe sensor. One method to reduce the diffusion time of the chemicals inthe fluid is to reduce the diffusion length. It has been realized thatthe diffusion length may be reduced by flowing a higher proportion ofthe sample a closer distance to the capture molecules. Specifically, ithas been found that the diffusion time may be reduced by flowing asample fluid through a relatively narrow-size pore having capturemolecules immobilized on its surface. This causes the mean distancebetween target chemicals and capture molecules in a set volume of samplefluid to be reduced with respect to flowing the same volume of samplefluid over a planar surface comprising capture molecules.

Referring now to FIG. 1 , an example three-dimensional chemical sensingsystem 100 is provided. The chemical sensing system 100 comprises afluidic cartridge 104, an inlet port 102, a signal processor 114, alight source 108 for LSPR measurement, and a detector 110. The chemicalsensing system 100 may further comprise an outlet reservoir 122 and afluid driving element such as a pump 112 or pressure source (not shown).

The pump 112, the light source 108, and the detector 110, may beelectrically powered, for example, by a battery, a power outlet, or acombination of both. The chemical sensing system 100 may be locatedwithin a housing (not shown), for example, a portable housing such as ahand-held housing.

Inlet port 102, which is in communication with a fluid inlet 116, isoperable to receive a fluid sample, for example from a syringe, and feedthe fluid sample to the fluid inlet 116. The inlet port 102 may furthercomprise, or be linked to, a filter or mixing element to filter,pre-treat or mix a sample fluid.

The inlet port 102 may vary in form depending on the type of fluidsample that is being tested. For example, in the case of a blood samplefor biological diagnostics, a sterile needle in a lancing device may beemployed to obtain the sample similar to a glucose monitor. It will beappreciated that the inlet port 102 may comprise various other formsincluding Luer taper fittings, press fittings, or an open reservoir. Itwill be appreciated that the inlet port 102 may be built into thefluidic cartridge 104.

Referring now to FIGS. 2 and 3 , the fluidic cartridge 104 comprises afluid inlet 116, a sensor 106, and a fluid outlet 118. The fluid inlet116 is fluidically connected to the sensor 106 and thereby, operable todeliver fluid to the sensor 106 to cause one or more target chemicals inthe sample fluid to bind to capture molecules in the sensor 106, as isfurther described herein. It will be appreciated that the same samplemay be transported to two or more sensors, for example, in a multiplexeddesign as demonstrated below with reference to FIG. 7 .

The fluidic cartridge 104 may be disposable or designed for repeateduse. The fluidic cartridge is composed of a material that issubstantially optically transparent in the LSPR wavelengths being used.For example, polydimethylsiloxane (PDMS), is optically transparent overmany LSPR wavelengths. In the example of FIG. 3 , the sensor 106 issandwiched between two layers of PDMS. Other transparent materials couldbe used to form the fluidic cartridge including, glass, poly(methylmethacrylate) (PMMA), cyclic-olefin polymer, or another material throughwhich micro-channels may be formed to produce the fluid inlet 116 andthe fluid outlet 118.

The fluid outlet 118 is also fluidically connected to the sensor 106 toreceive fluid from the sensor 106 and allow fluid to egress from thesensor 106. Optionally, the fluid outlet 118 may deliver, to the outletreservoir 122, fluid that has passed through the sensor 106.Alternatively, the fluidic cartridge 104 may retain the sample.

Although the fluid inlet 116 and fluid outlet 118 are shown in thesimplest form in FIG. 3 , the fluid inlet 116 and fluid outlet 118 maytake different routes through the fluidic cartridge depending onspecific requirements such as flow rate and sample volume or the needfor mixing and pre-treatment steps. The dimensions and path of the fluidinlet 116 and fluid outlet 118 may be chosen depending on the desiredfluid speed and mixing properties.

A pump 112, or other fluid driving element, may optionally drive thefluid from the inlet fluid channel 116, through the sensor 106 and outof the fluidic cartridge through the fluid outlet 118. For example, thefluid driving element may also comprise a pressure source or a vacuumsource at the outlet port 118. The pump 112 can be controlled by thesignal processor 114 or other controller. The direction of fluid flowcan be rapidly and automatically switched via software control to movethe sample back and forth transversely through a membrane in the sensor106, allowing for prolonged interaction times with a small samplevolume, thereby potentially increasing the performance of the sensor106.

Alternatively, the fluid may be driven through the sensor 106 using, forexample, electro-osmotic pumps, gravity, wicking of a membrane, or bedriven by a syringe or other fluid source at the inlet port 102.

The signal processor 114 comprises, or is linked to, a memory, aprocessor, and a user interface which may include a display and an inputdevice such as a touch screen or keyboard and mouse. The signalprocessor 114 may be linked to another input device, for example, abarcode scanner, an RFID scanner, or an NFC reader to identify a fluidiccartridge comprising an identifier, for example, a barcode, RFID tag, orNFC chip. It will be appreciated that other identification methods maybe used including, for example, image analysis or a simpleidentification code which may be entered by the user. The identifier maycomprise, or be linked to fluidic cartridge information such as relevantstandard curves, the type of sensor being used, manufacturing date, etc.

The signal processor 114 may, in various examples, comprise a computersuch as a laptop computer, desktop computer, microcomputer, cloud-basedprocessor, or a mobile device. The memory of the signal processor 114may contain fitting algorithms and standard curves. The signal processor114 may be linked to one or more of the pump 112, light source 108, ordetector 110 via a wired connection, for example a local area network orUSB connection. Alternatively, or in addition, signal processor 114 maybe linked to one or more of the pump 112, light source 108, or detector110 via a wireless connection such as Bluetooth, Wi-Fi, or cellularconnection. In some embodiments, the signal processor 114 may be locatedremotely from the fluidic cartridge 104.

The signal processor 114 may control the light source 108 to emit lightinto the sensor 106. An example light source 108 comprises a white lightemitting diode (LED) and is coupled to a detector 110 comprising aUV-visible spectrometer. White light sources other than LEDs such ashalogen bulbs and others such as red, green, and blue LEDs separate orcombined together, may also be used. A light source for the visiblerange (400-800 nm) could be a white light source such as a halogen bulbor an LED, a combination of colored LED light sources such as red, blue,and green, a single colored LED light source, or a laser at a specificwavelength. For operation below the visible range (100-400 nm) of thespectrum, an ultraviolet (UV) light source such as a UV LED could beused. For operation above the visible range (800-2500 nm) an infrared(IR) source such as an IR LED could be used.

The detector 110 may comprise a charge coupled device, a photodetector,a spectrometer, a photodiode array, or a combination thereof, to obtainLSPR light intensity readings. The detector 110 may comprise aspectrometer or photodetector designed for parts of the electromagneticspectrum outside the visible range, including the ultraviolet (UV)range, the near infrared (NIR), or IR range. The detector 110 maycomprise a combination of two types of detectors, for example, aphotodetector and a spectrometer. The detector 110 is selected incombination with an appropriate light source 108.

The light emitted by the light source 108 is transmitted though thefluidic cartridge 104 and sensor 106 and is received, at least in part,by a detector 110. As mentioned above, the fluidic cartridge 104 andsensor 106 must be at least partially transparent to the LSPRwavelengths emitted by the light source 108. The detector 110 generatesa transmission signal, for example a digital transmission signal, basedon the light transmitted through the sensor 106 and provides the signalto the signal processor 114. The signal processor 114 is operable toproduce a spectrograph based on the transmission signal. The signalprocessor 114 may also be operable to select an output based on apredetermined transmission signal or a comparison between thetransmission signal and one or more reference signals or thresholds. Forexample, the signal processor 114 may output the concentration of atarget chemical based on a transmission signal that is consistent withone or more reference signals, or exceeds a threshold of an establishedreference signal. The signal processor may also be used to determinebiointeraction analysis parameters between the target and capturemolecule, which may include reaction kinetic information (on and offrates), affinity, and specificity. A simple photodetector may be used tomeasure intensity changes due to the spectra shifts.

In the example of FIG. 1 , the sensor 106 is substantially planar and islocated laterally between the path of the light source 108 and thedetector 110. As a sample fluid flows through the sensor, the lightsource 108 emits light and the spectrometer 110 receives lightcontinuously, or at predetermined intervals, to monitor changes in theresonance peak of the detected light. The light source 108 and detector110 may be arranged for maximal illumination of the sensor and maximalcapture of the light transmitted through the membrane, respectively.FIG. 1 shows a transmission based LSPR arrangement, wherein the lightsource 108 shines through the membrane and to the detector 110.

It has been found that to address, at least in part, the sensitivity ofLSPR-based chemical detection, a three-dimensional porous membrane isused as a substrate for sensor 106. Functionalized metal nanoparticlesare immobilized within the pores of the membrane and a sample is flowedthrough the pores. Such a sensor design may be referred to herein as atransmission-based three-dimensional sensor (T3D). The three-dimensionalporous membrane is substantially transparent for the wavelengths ofincident light that are used to obtain a signal.

Turning to FIGS. 4A and 4B, the sensor 106 comprises a nanoporousmembrane. Pores 148 of the membrane comprise functionalized metalnanoparticles 150 immobilized on their surfaces. Specifically, themembrane is characterized by nanopores, which are channels 10 nm-1000 nmin diameter and can be up to 200 μm long. For example, the nanoporousmembrane may comprise pores that are about 25, 50, 100, 150, 200, 250,300, 350, 400, 450, and 500 nm in diameter, and about 1, 5, 25, 50, 75,100, 150 and 200 μm in length.

A sample is flowed through the pores 148 of the membrane, which haverelatively small diameters. The relatively small pore diameters, forexample about 100 nm, limits the diffusion distance between the chemicaltargets and their corresponding capture molecules on the nanoparticlesurface, thereby reducing the mean diffusion time required for a targetchemical to reach a capture molecule. By reducing the diffusion time,the time required for the target-capture molecule system to reachequilibrium may be decreased. The nanoparticles may also be bound to thetop and bottom surfaces of the nanoporous membrane.

The working area of a sensor is limited to the width of the coherentlight source, which may be approximately 1-4 mm. It is thereforeimpractical to increase the sensitivity of sensors of the prior artsimply by creating a larger planar (two-dimensional) sensor. However,because functionalized nanoparticles are immobilized onto pore surfacesin a three-dimensional membrane, the number of nanoparticles over agiven sensor area can be increased with respect to a similartwo-dimensional design. In many cases, the number of nanoparticlesimmobilized within a given sensor area may be increased substantiallywith respect to a two-dimensional design.

The membrane may be selected to optimize the thickness, pore size, andpore periodicity for a particular chemical sensing application. Thediameter of the sensing membrane can be selected based on cost andperformance. In an example, the diameter of the sensing membrane may beas small as 1 μm or as large as 13 mm. The light beam size may be closeto the diameter of the sensing membrane to maximizing the strength ofthe absorbance signal. The diameter of the sensor may be small to reducecost.

Anodized aluminum oxide (AAO) is an example nanoporous membranematerial. The dimensions of nanopores in an AAO membrane may becontrolled when producing the AAO material. The material is sufficientlyoptically transparent at LSPR wavelengths to allow fortransmission-based spectroscopic measurements to be performed. Thetransmission of light through the membrane is dependent on severalfactors including pore size and thickness that impact the absorbance ofthe membrane material and the scattering it produces in the LSPRwavelengths of interest.

Although both reflection and transmission measurements are possible withthis system, is has surprisingly been found that transmissionmeasurements provide better results than reflection measurements. Inreflectance mode the reflection off of the top surface of the membraneis strong, and accounts for the majority of the signal returning to thedetector. This reflected light carries very little nanoparticleabsorbance information with it as it is only interacting with thenanoparticles on the top surface of the membrane. In transmission mode,the majority of the light passes through the entire thickness of themembrane before it reaches the detector, interacting with all of thenanoparticles throughout the entire thickness of the membrane. Thisgreatly increases the absorbance component caused by the nanoparticles,increasing the signal to noise ratio and thereby increasing sensorperformance. This also ensures that the measured signal is from targetbinding sites throughout the membrane rather than just those at the topsurface. It has further been discovered that a larger proportion ofscattering light reaches the detector in reflection mode versustransmission mode, increasing the noise. Also, the AAO pores act as awaveguide, allowing light to propagate within the pores and providingenhanced interaction with the nanoparticles, resulting in unexpectedlyhigh transmission of light with a large LSPR absorbance component,providing further enhancements to the transmission signal which are notobtained when employing reflection signal. FIG. 16 illustrates thedramatic improvement in the LSPR signal when measuring in transmissionversus reflection.

However, a transmission system is more difficult to build as the LSPRwavelengths must be matched to the AAO properties to allow sufficientlight transmission. Variables such as pore size, and thickness may betuned depending on the wavelengths used so as not to interfere with theoptical signal generated by the immobilized metal nanoparticles. Thetransmission apparatus can be realized by having a light source on oneside of the membrane and a detector on the other side of the membrane.It is also possible to make a pseudo-transmission setup with the lightsource and detector on the same side of the membrane, if a highlyreflective surface is placed beneath the membrane. The reflectivesurface will cause the transmitted light to travel back through themembrane and to the detector on the opposite side, which is effectivelya transmission measurement.

In FIG. 17 and FIG. 18 , the transmission of various AAO membranes withdifferent pore sizes and thicknesses have been measured both dry and wetwith water. In general, smaller pores result in higher transmissioncompared to larger pores. With respect to thickness, thinner membranes(50 um) have higher transmission compared to thicker membranes (100 um),but the impact is not as significant as pore size. To use AAO as amaterial in this sensor, the pore size and thickness should be selectedto be as small as possible while still allowing the nanoparticles to fitinto the pores without blocking them. Now examining the dry vs wetmembranes, the transmission through wet membranes is improved, due torefractive index matching, especially for membranes with larger poresizes (100 and 150 nm). To get the best results, measurements should betaken while the membrane is wet. To further improve the transmission, ahigh refractive index solution can be introduced after the sample haspassed through the sensor. The high refractive index solution willreduce scattering even further, improving the signal to noise ratio.

Any optical signal that is generated by the membrane itself can beremoved from spectroscopic measurement by the signal processor 114 usingbaseline correction methods. A reference measurement of an area of themembrane which is not coated in nanoparticles may be taken to subtractout the optical signature of the membrane using the processor 114, whichmay enhance the signal produced by the nanoparticles. Pores of amembrane, for example an AAO membrane, can be chemically treated toallow metal nanoparticles 150 to be associated with its surface. Forexample, the chemicals used to treat AAO include, but are not limitedto, polyelectrolytes such as polyallylamine hydrochloride (PAH) andpoly-(succinyl-sulphonate) (PSS) that can create a positive or negativeelectrostatic charge on the AAO surface. Metal nanoparticles stabilizedin water by charged surface groups can be associated to the membranethrough electrostatic forces. Other methods to immobilize nanoparticlesinclude using a silane based linker, which will covalently bind to thesurface of the AAO. For example, a silane-thiol molecule could be used,with the silane covalently binding to the AAO pore wall and the thiolcovalently binding to the nanoparticle. The thiol could be replaced withany chemical group that associates to the nanoparticle surface, such asan amine group, for example. The AAO may be pretreated to generatehydroxyl groups on the surface of the pores to promote silanization,through a procedure such as incubation in a 1:1 solution of hydrochloricacid and methanol for 30 minutes, or any other method that can be usedto generate hydroxyl groups the surface.

It will be appreciated that various other nanoporous membrane materialsmay be used including various organic and inorganic membranes that areat least partially transparent at the LSPR wavelengths of interest.Advantageously, metal nanoparticles may be associated directly to thesemembranes if the membranes contain thiol-, amide-, phospho- or otherfunctional groups.

The membrane material could also be chemically treated withpolyelectrolytes such as PAH, PSS or other charged polymers to associatethe metal nanoparticles to the surface through electrostaticinteractions. Reaction chemistry such asN-Hydroxysuccinimide/ethyl(dimethylaminopropyl) carbodiimide (NHS/EDC)coupling among other coupling chemistries may also be used to bind themetal nanoparticles to the surface. It will be appreciated that thereexist other methods of immobilizing functionalized metal nanoparticles150 to an optically transparent nanoporous material.

Turning now to FIG. 4C, an example of functionalized metal nanoparticles150 functionalized to a pore surface of an AAO membrane is provided. TheAAO membrane 154 has a bilayer of charged polyelectrolyte 156 on itssurface that facilitates the association of charged metal nanoparticles150 to the walls of the pores.

The metal nanoparticles shown in the example of FIG. 4C have twodifferent metal core shapes, a sphere 160 and a rod 162, which may beused together or independently. Both are functionalized with antibodies164 as the capture molecule with their distinctive Y-shape and form aself-assembled monolayer (SAM) on the surface of the nanoparticle.Blocking molecules 166 prevent non-specific binding to empty bindingsites on the metal surface. The capture molecules may also compriseaptamers, polymers, or DNA

The SAMs may comprise an antibody, aptamer, polymer, DNA or othercapture molecule that is bound to the nanoparticle 150 surface andcapable of selectively binding to the chemical of interest. In the caseof gold nanoparticles, this binding typically occurs spontaneouslybetween the gold surface and thiol groups that are natural to thecapture molecule or have been chemically added to the capture moleculeor nanoparticle surface.

To prevent non-specific binding of non-target chemicals, inert blockingmolecules are used to pacify empty binding locations on the nanoparticleand pore surfaces. Blocking molecules for metal nanoparticles maycomprise thiolated compounds with inert end groups that provide aqueousstability such as carboxyl, methyl, or polyethylene glycol (PEG). Forthe pores, blocking molecules may be silane based compounds with inertend groups such as carboxyl, methyl, or PEG. Bovine serum albumin (BSA)is another example of a possible blocking molecule that may be used onnanoparticle and pore surfaces. Together, the capture and blockingmolecules form a SAM that imparts functionality onto the metalnanoparticle.

To create a functional sensor 106, the metal nanoparticles are firstimmobilized on the nanoporous membrane surface then the nanoparticle isfunctionalized with a SAM. Alternatively, the particle may first befunctionalized with a SAM and the nanoparticles may be immobilized onthe membrane.

The size, shape and elemental composition of metal particles affect thelocation and intensity of the LSPR absorbance peak in theelectromagnetic spectrum. As such, the size, shape, and composition ofnanoparticles are selected to allow for a measureable transmissionsignal through the nanoporous membrane. The size and shape of thenanoparticles are also selected to avoid physical clogging of the poresof the selected sensor membrane.

Various metal nanoparticles have different bulk refractive indexsensitivities and electromagnetic decay lengths, which may be tuned toproduce the optimal LSPR sensor response for a given capture-targetsystem. Decay length and sensitivity are typically not independentparameters, and both can be tuned with the size, shape, and compositionof the nanoparticle. For example, increasing the size of a sphericalnanoparticle increases both the sensitivity and the decay length. Othernanoparticle shapes may have different trends with respect to size,sensitivity, and decay length. Preferably, a nanoparticle will have thehighest sensitivity with a decay length that is similar to the thicknessof the capture molecule-target complex. For example if the total size ofthe capture molecule-target complex is 8 nm, the optimal decay lengthwould be near 8 nm. As such, the size, shape, and composition of thenanoparticle can be tuned based on the sensitivity and decay lengthparameters for a particular capture molecule-target complex. This alsomust correspond with the necessary optical properties to allowsufficient transmission of the LSPR signal through the membrane.

Therefore the nanoparticles can be selected depending on the one or morespecific chemical target being investigated by the sensor 106.

Compositions of metal nanoparticles that can be used for LSPR includegold, silver, platinum, gold coated silver, silver coated gold,combinations of these metals, and others. The shape of the nanoparticlesused can also vary. Useful nanoparticle shapes include but are notlimited to, rods, stars, urchins, decahedra, hexagons, triangles,shells, prisms, platelets, spheres, rice, plates, cubes, cages, starsand bipyramids. The dimensions of the metal nanoparticles can rangebetween about 1 nm and 1000 nm with a variety of area to volume ratios.

Referring now to both of FIGS. 4C and 4D, a combination of two or moretypes of nanoparticles may be immobilized on the surface of a singlemembrane. Each of the nanoparticle types may have been functionalizedwith a specific capture molecule. For example, nanoparticle 150 may befunctionalized with capture molecules to capture a first target chemicalwhereas nanoparticle 151 may be functionalized with capture molecules tocapture a second target chemical.

With a combination of different nanoparticles (shapes, sizes and/ormetals) functionalized to capture different targets, antibodies on thespherical nanoparticle may be selective to different targets fromantibodies on the rod nanoparticle, each nanoparticle producing adistinct signal. Therefore, the concentration of each target can bedetermined from a single absorbance spectrum if the spectrum from eachof the different particles does not overlap to such a degree thatdeconvolution of the peaks is impossible. Various particles are used toallow the detection of multiple targets on a single membrane. FIG. 19shows two different particles immobilized in the same membrane, one witha resonance at approximately 495 nm and the other with a resonance atapproximately 580 nm. The two peaks are clearly distinguishable and canbe used for generating two independent signals from a single sensor. Anycombination and any number of nanoparticles with different LSPR peakpositions may be used to achieve multiple measurements. Theincorporation of multiple particles with different LSPR peak positionswithin a membrane allows for a higher density of each particle to bepresent compared to the case if multiple particles were incorporatedonto a planar substrate. Higher particle densities may offer bettersensor performance due to high signal to noise ratios. This system mayallow detection of multiple targets using a small initial sample whichmay be very advantageous in the case where sample is limited ordifficult to obtain. Detecting multiple targets in tandem may also speedthe time to obtaining results.

Various particles could also be attached to distinct areas of the samemembrane using a tool similar to a protein spotter or variousmicrochannels to allow geometrical separation of the particles. This isadvantageous if using a photodetector rather than a spectrometer, or ifcross reactions may occur between particles due to their chemicallymodified surfaces. The use of different particles on a single membranecan also facilitate the use of a control sensor to compensate for errorsinduced by non-specific binding, temperature change, bulk refractiveindex change, or other factors. This could be achieved byfunctionalizing one nanoparticle with a capture molecule and blockingmolecule, and functionalizing a second particle with only a blockingmolecule similar to the blocking molecules used in the firstnanoparticle. Any peak changes that are detected from the secondnanoparticle are erroneous, and as such, the second nanoparticle acts asa control. The different nanoparticles may be spectrally distinct orgeometrically distinct.

Nanoparticles are immobilized onto the membrane walls through contactbetween the walls and a colloidal nanoparticle mixture. To permeate thenanoparticles throughout pores of the membrane, a variety of techniquesmay be employed. The nanoparticles may be physically pumped through themembrane, they can be driven into the membrane through the use ofelectrical potential, and they could enter by diffusion among, othermethods.

The metal nanoparticles must remain relatively dispersed whileimmobilized in the pores, as extensive aggregation will affect thequality of the measurements due to peak broadening or pore clogging. Ithas been discovered that in order to improve the penetration anddispersion of the nanoparticles throughout the membrane pores, surfacestabilizing additives can be included in the colloidal nanoparticlemixture. Alternatively, or in addition, the additives may be appliedbefore the nanoparticles are immobilized on the membrane by pumping orincubating the additives through the membrane before the colloidalnanoparticle mixture is applied. It has been discovered that surfaceblocking additives are especially important in order to immobilize largenanoparticles into small pores. For example, AAO membranes with 100 nmpores were treated with PSS then PAH to render the surface positivelycharged. Gold nanoparticles 20 nm in diameter and coated in negativelycharged citrate were pumped through the PSS/PAH coated membrane. No goldparticles were observed to bind to the AAO pores. Upon addition of 0.01%BSA to the 20 nm gold colloidal solution and pumping through themembrane, gold nanoparticle binding was observed on the AAO pores. It ishypothesized that the zwitterionic nature of BSA acts to help stabilizethe nanoparticles, possibly by screening the charges at the top surfaceof the AAO membrane, allowing the nanoparticles to more easily enter andtravel through the membrane. In another experiment, a PSS/PAH modified150 nm AAO membrane was dipped into a 1% BSA solution and rinsed withwater. A 20 nm gold colloidal solution, without any BSA additive, waspumped through the membrane, and nanoparticle binding was observed.Binding was observed in the pores at a high density, with a low densityof binding on the membrane surface. Increasing the BSA dip concentrationto 10% caused a reduction in the binding density of the nanoparticleswithin the pores, with almost no nanoparticles present on the surface ofthe membrane. A control experiment was done on glass with a coating ofPAH. BSA at 0.01% was incubated in a small droplet on the surface of theglass and rinsed away. A 20 nm gold colloid solution was then applied tothe glass. Nanoparticle binding was observed to occur in areas in whichthere was no BSA, demonstrating that BSA may prevent the nanoparticlesfrom binding to the PAH treated surface. This is shown in FIG. 22 . Afinal experiment was performed with a PSS/PAH modified 150 nm membranedipped in 1% BSA. 0.001% BSA was added to the gold colloid solution andpumped through the membrane. Binding was observed in the pores and onthe surface but at a lower density than without the BSA additive. BSA,acting as a surface blocker, can be used to reduce membrane surfacebinding, helping to prevent agglomeration. BSA can also act as astabilizer, allowing larger particles to more easily enter smallerpores. As we have demonstrated, smaller pore sizes are more transparentand so may be preferable to use. Also, larger nanoparticles have highersensitivities, so they may also be preferable to use. So the use ofsurface stabilizing additives may allow a better sensor to befabricated. Other possible additives include various inorganic salts,various surfactants such as Tween 20 or Triton X, or PEG, along with avariety of other potential molecules and combinations. It is alsoassumed that these additives will have similar effects when othernanoparticle binding methods are used other than charge interactionsbased on PSS/PAH, such as covalent methods using thiol chemistry asdescribed previously.

The nanoparticles may be functionalized with capture molecules before orafter they are immobilized on the pore walls. If they are immobilizedprior to being functionalized, they can be immobilized on the pore wallsthrough electrostatic interactions or using functional groups bound tothe membrane that would be capable of binding to the nanoparticles, forexample, in the case of a gold surface of a nanoparticle a thiolatedpolymer may be used. If the nanoparticles are functionalized prior tobeing immobilized, as they may be in the case of a multiplexed sensor,for example, a functional group would be used.

Alternatively, nanoparticles 150 and 151 may be functionalized tocapture the same target chemical and any difference in signal could beused to generate a baseline signal, thereby removing uncertainty in thesignal.

Turning to FIG. 5 , an example process for sampling a fluid is provided.In step 184, a sample fluid enters the inlet port 102. In 186, the pump112 drives the sample into the fluidic cartridge 104 and the sampleflows through the sensor 106 in step 188. In step 190, the light source108 emits light onto the sensor 106 in the fluidic cartridge 104, whichcauses LSPR interactions in 192. In 194, the detector receives lighttransmitted though the sensor 106, measures the light intensity andwavelength in 196 and generates a transmission signal in 197. In 198,the signal processor 114 determines whether a shift in the resonant peakis observed and in 199, detects the presence and/or determines theconcentration of the target chemical in the sample based on the resonantpeak shift, as described above.

Referring now to FIG. 6 , the change in peak position or intensityinduced by binding of the target chemical to the capture probe can bemonitored in real time or by comparing the peak position prior to thetarget chemicals binding to the capture molecules in the sensor 106 withthe peak position after the target chemical has bound to the capturemolecules in the sensor 106. This binding may be referred to as abinding event.

The change in peak position can be compared to data obtained from astandard curve of peak change vs. concentration by the signal processor114, and using a fitting algorithm the presence of a target chemical ina sample may be detected, and the concentration of the target in thesample may be determined, by the signal processor 114. Alternatively, orin addition, the rate of change (the slope) of the signal may be used tomore rapidly determine the concentration by comparing the calculatedslope to data obtained from a standard curve of slope vs. concentration.Various data processing mechanisms may be employed by the signalprocessor 114 during data collection to improve the signal to noiseratio of the optical signal, such as smoothing and averaging functions.High speed acquisition is used to facilitate real time averaging andsmoothing. Various peak fitting algorithms may be employed that offer ahigh level of stability in the peak position.

An indication of whether a target chemical was detected may be output bythe signal processor 114. The indication may be output, by way ofexample, on a display, as an indicator light, as a warning signal, or asan electronic message. Alternatively, or in addition to the indication,the concentration of the target chemical may be output by the signalprocessor 114 or on a display linked to the signal processor such as thedisplay of a cellular phone. Results of assays can be stored in built inmemory on the device, on peripheral devices, or stored in a cloud-basedserver.

The spectrometric optical measurements taken through the membrane exposethe surface area of the membrane and all of the particles containedtherein, and hence, the sensor may be referred to as a three-dimensionalsensor. A single sensor 106 may be adapted to detect multiple targetswithin a single fluid sample through the inclusion of multiple membranesor functionalized particles with different shapes, sizes or metals.

A multiplexed design for the fluidic cartridge is provided in FIG. 7 .The inlet 116 is split and leads through several independent sensors106, which are fluidically connected to the outlet 118. The sensors 106are oriented to allow light transmission and spectrometric measurement.A multiplexed design can also be achieved using several fluidicmicrochannels coming from a single channel that carry the sample throughdifferent areas of the same membrane that have been functionalized forthe same or different targets.

Multiplexed measurements can be taken with multiple light sources andspectrometers (or other light measurement mechanisms such as aphotodetector), a multiplexed spectrometer such as a hyperspectralimager, or by moving the chip to align each sensor under a single lightsource using the chemical sensing system 100 shown in FIG. 1 . The flowthrough a multiplexed fluidic cartridge may be controlled by a singlepump 112, however, designs that employ multiple pumps or othercomponents to facilitate flow may also be used.

FIG. 8 is a scanning electron microscope (SEM) image of 20 nm goldnanoparticles 172 immobilized in the pores 170 of a 200 nm pore size AAOmembrane. This figure demonstrates that the metal nanoparticles 172 maybe immobilized throughout the pores 170 in a substantially dispersedmanner. An agglomeration 174 is also shown on the surface of the pore170 which may result if surface stabilizing additives are not employed.

FIGS. 9A and 9B, 10, 11, 16, 20, and 21 illustrate advantages of anexample three-dimensional AAO membrane in comparison with conventionaltwo-dimensional sensors. The glass slide of FIG. 9A comprises goldnanoparticles immobilized onto its surface. In contrast, the membrane ofFIG. 9B is an AAO membrane comprising gold nanoparticles immobilized onthe surface throughout its pores. The red appearance of both images isdue to the LSPR of the immobilized gold nanoparticles. The AAO membraneappears as a very dark red in comparison to the glass slide due to thelarger number of immobilized gold particles per given unit of sensorsurface area. Therefore, for each given unit of surface area, there is astronger LSPR interaction due to the greater number of immobilizednanoparticles.

FIG. 10 is a chart of the absorbance spectrums of the glass slide withrespect to the AAO membrane of FIGS. 9A and 9B, respectively, taken inabsorbance mode. The absorbance peak of the AAO membrane isapproximately 6 times larger than the glass slide absorbance peak, whichdemonstrates that an AAO membrane may accommodate a higher number ofgold nanoparticles, and therefore, may accommodate a higher number ofaccessible capture molecules with respect to a planar glass slide.

FIG. 11 is a plot showing the simulated response of a sensor based on aglass slide (the conventional LSPR design) with respect to a sensorbased on an AAO membrane, which may also be referred to herein as atransmissive three-dimensional (T3D) LSPR design (New T3D LSPR Design).Although not directly visible from the plot of FIG. 11 , the detectionlimit of the sensor comprising the AAO membrane at (2 pg/ml) has beenpredicted by computer simulations to be improved by approximately 1000times when compared with the 2D arrangement (2000 pg/ml).

FIG. 12 is an example procedure for immobilizing gold nanoparticles onan AAO membrane. FIG. 13 shows the effect of immobilizing goldnanoparticles on a 13 mm AAO membrane without the use of surfacestabilizing additives to prevent agglomeration. Agglomeration isparticularly apparent on the outer surfaces of the membrane surface,i.e., the portions of the membrane between the pores. The goldnanoparticles agglomerate on the exterior surface of the membrane. Thesurface agglomeration makes the membrane ineffective. For reference,FIG. 14 is an example AAO membrane that has not been immobilized withgold nanoparticles. FIG. 14 may be compared with FIG. 9B to observe thedifferences between a clean AAO membrane and an AAO membrane with goldnanoparticles properly immobilized according to the procedure providedherein.

Referring to FIG. 15 , a method to enhance the LSPR shift for smallmolecule targets is outlined. For small molecular weight chemical targetdetection, for example ions or hormones, chemicals, DNA, RNA, aptamersor polymers 202 may not be effective without modification. However, aheavy molecule 204, such as a globular inert protein (bovine serumalbumin), an inert heavy chained polymer or a surface inactivated smallnanoparticle could be bound to the free end of the capture molecule 202which may comprise, for example, an aptamer or capture polymer. When thetarget 203 comes into contact with the capture molecule 202, the capturemolecule changes its conformation at 205, thereby bringing the heavymolecule 207 closer to the immobilized nanoparticle 201 surface. Thisenhances the LSPR effect that will be detectable by the spectrometer andallow for the detection of small chemical targets.

Another method of enhancing the LSPR signal for the detection of verysmall targets or targets at very low concentrations is the inclusion asignal-enhancing molecule that can be pumped into the mixture aftertarget binding has taken place or mixed with the target prior to targetbinding. This is similar to the sandwich assay concept used in ELISA,where an immobilized antibody captures the target of interest and then asecond molecular dye-labelled antibody is added to bind to the nowimmobilized target and signal its detection through fluorimetry. Toadapt this concept to the sensor 106 as described herein, the samplefluid is pumped through the sensor and capture molecules on thenanoparticles bind the target chemicals. A secondary mixture ofsolution-based molecular dye labelled capture molecules are pumpedthrough the sensor and bind to the captured targets. An energy transferprocess occurs to enhance the LSPR effect due to the dye molecules beingbrought into close proximity with the metal nanoparticles. This mayproduce a larger absorption peak shift to be measured by the detector110.

The incorporation of shift enhancers can also be used to improve thedetection of chemicals. For example, a secondary capture molecules couldbe introduce to bind to the target after it has bound to thenanoparticle surface through the primary capture molecule. This wouldenhance the LSPR shift due to the enhanced localized change in therefractive index due to the additional mass. Another alternatives topotentially enhance the shift of the resonance peak is the addition ofother enhancer entities, such as free-floating polymer or metalnanoparticles functionalized with secondary capture molecules, after thetarget chemicals are bound to the capture molecules in the sensor 106.Such entities would be made of materials with a high refractive indexand molecular weight to allow a significant enhancement of the signalshift when they bind to the target. Metal particle enhancer entitiescould be made of an LSPR generating material to further enhance theresonance shift by resonance coupling. The entities could also be amagnetic material such as iron oxide, which has a very high refractiveindex and molecular weight. They could also be metal coated polymerparticles, polymer coated metals particles, polymers particles, or metalparticles.

Another method to enhance the performance of the LSPR sensor is tochoose nanoparticle and pore sizes that cause the particles to be closeenough together so that their three dimensional electromagnetic fieldsoverlap. When this occurs, a single binding event on the surface of onenanoparticle will result in changes to its own electric field inaddition to changes in the electromagnetic fields of those neighbouringnanoparticles close enough to have their fields overlap. This willresult in a larger response from a single binding event, increasing thesignal change.

In one embodiment of the invention there is provided a self-referencingsensor for simultaneously sensing analyte and reference signals. Thereference signal can then be used to subtract out the non-specificeffects observed in the detection signal obtained from the analyte.

In one embodiment the nanoparticles are supported on a substrate inanother embodiment the nanoparticles are in a solution, suspension ordispersion.

In one embodiment, the invention is directed to a self-referencingsensor apparatus employing a sensor composed of at least onenanoparticle type that is capable of providing multiple signalssimultaneously. Specifically, the nanoparticle type(s) are selected suchthat at least two distinct LSPR peaks are produced and can be measuredby a single detector. The nanoparticles can be functionalized with acombination of various capture molecules and blocking molecules toprovide both a specific detection signal as well as a reference signalsimultaneously.

In one embodiment the self-referencing sensor comprises a first type ofnanoparticle having a distinct LSPR signal functionalized to bind to ananalyte and a second type of nanoparticle having a distinct LSPR signalthat is different than the signal of the first type of nanoparticle. Thesecond nanoparticle is functionalized to block binding with the analyte,thereby acting as a reference signal. A signal processor may then beused to subtract the reference signal from the analyte signal.

Referring to FIG. 23 , an example of a sensor containing nanoparticlesin solution is shown. The sensor contains one or more nanoparticle typesin a colloidal dispersion that would produce at least two distinct LSPRpeaks. Each nanoparticle type can be non-functionalized, functionalizedwith capture molecules, functionalized with blocking molecules, orfunctionalized with a combination of any capture molecules and blockingmolecules. At least one nanoparticle type must be able to specificallybind to an analyte of interest. In the example shown in FIG. 23 , thesensor contains three nanoparticle types, each functionalized with aunique capture molecule or blocking molecule. The two nanoparticles withcapture molecules would be capable of detecting two different types offree molecules through specific interactions, whereas the blockednanoparticle would provide the reference signal.

Referring now to FIG. 24 , an example of a sensor containingnanoparticles on a substrate is shown. The sensor may contain one ormore nanoparticle types that are immobilized onto a substrate that wouldproduce at least two distinct LSPR peaks. In FIG. 24 two nanoparticletypes are shown, each nanoparticle type can be non-functionalized,functionalized with capture molecules, functionalized with blockingmolecules, or functionalized with a combination of any capture moleculesand blocking molecules. At least one nanoparticle type must be able tospecifically bind to an analyte of interest. FIG. 24 shows a firstnanoparticle type with blocking molecules and a second nanoparticle typewith capture molecules and blocking molecules. In this example the firstnanoparticle type would provide a reference signal and the secondnanoparticle type acts as an analyte sensor.

When used in transmission mode, the sensor substrate will be at leastpartially transparent to allow for the light source to pass through thematerial and reach the detector such that the LSPR response of thenanoparticles can be measured. The substrate can be, but is not limitedto, a planar surface such as glass, plastic, quartz, titania orsilica-based materials, or can be a three-dimensional porous materialsuch as anodized aluminum oxide.

The nanoparticles may be immobilized onto the substrate by directdeposition, or through the use of an adhesive layer on the surface or asurface functionalization as shown in FIG. 24 . This includes but is notlimited to immobilization through covalent bonds, electrostaticinteractions, hydrophilic/hydrophobic interactions and/or Van der Waalsforces between the nanoparticles and the surface. The nanoparticles canbe deposited in a monolayer or multi-layer structure on a variety ofsurface morphologies. The nanoparticles can also be fabricated using topdown processing methods such as nanoimprint lithography, UV lithography,or electron beam lithography.

Different nanoparticle types refer to nanoparticles that vary either incomposition, size and/or shape. Typically metal nanoparticles are usedto produce an LSPR signal. Compositions of metal nanoparticles that canbe used for LSPR include but are not limited to gold, silver, platinum,copper, gold coated silver, silver coated gold, combinations of thesemetals, and combinations of metal-coated non-metal nanoparticles. Usefulnanoparticle shapes include but are not limited to, rods, stars,urchins, decahedra, hexagons, triangles, shells, prisms, platelets,spheres, rice, plates, cubes, cages, stars and bipyramids. Thedimensions of the nanoparticles can range between about 1 nm and 1000 nmwith a variety of surface area to volume ratios.

The nanoparticles can be functionalized with capture molecules toprovide specific detection of another molecule or chemical of interest(analyte). Capture molecules that can be used include but are notlimited to chemical functional groups, aptamers, antibodies, DNA,nucleic acids, proteins, small molecules, or polymers. The surface ofthe nanoparticle may also act as capture molecules.

The nanoparticles can also be functionalized with blocking molecules.Blocking molecules are used to prevent nonspecific binding to thenanoparticle surface. They may often comprise thiolated compounds withinert end groups such as carboxyl, methyl, or polyethylene glycol (PEG)that provide aqueous stability. Bovine serum albumin (BSA) is anotherexample of a possible blocking molecule that may be used onnanoparticles.

Nanoparticle types can be functionalized with both capture molecules andblocking molecules. In this situation, the blocking molecules are usedto pacify empty binding locations on the nanoparticle surface, thuspreventing unwanted nonspecific binding.

There are many methods to immobilize and functionalize multiplenanoparticle types to create the sensors. These methods include, but arenot limited to: deposition of a colloidal mixture of multiplenanoparticle types in one step followed by selective or non-selectiveparticle functionalization, functionalization of the nanoparticles insolution prior to one-step deposition, functionalization of thenanoparticles in solution followed by multi-step deposition, ormulti-step deposition and functionalization of the nanoparticles. Theuse of such methods would be familiar to one of skill in the art.

Referring now to FIGS. 25A-B and FIG. 26A-C, showing the top view of anexample of a self-referencing sensor systems. The system is provided ina transmission based measurement setup. The sensor system is composed ofa light source, detector, and sensor which is interfaced with a fluidiccartridge. The fluidic cartridge comprises a fluid inlet, channel, and afluid outlet to deliver and egress the sample fluid containing one ormore target molecules to and from the sensor. The fluidic cartridge iscomposed of a material that is substantially optically transparent inthe LSPR wavelengths being used. The fluid inlet is fluidicallyconnected to the sensor and thereby operable to deliver fluid to thesensor to cause one or more target molecules in the sample fluid to bindto capture molecules in the sensor, as is further described herein.

In the example of FIG. 25A, a single sensor substrate is interfaced withthe fluidic channel. The single substrate contains at least one type ofnanoparticle, with at least one nanoparticle type being functionalizedwith a specific capture molecule. In the case where multiplenanoparticle types are used, the different nanoparticle types can beimmobilized onto the same area of the substrate, or onto distinct areasof the substrate within the optical path. FIG. 25B is an expanded viewof the substrate shown in FIG. 25A. The expanded view is a schematicdepicting the substrates with two types of nanoparticles.

In the example of FIG. 26 , multiple sensor substrates are interfacedwith the fluidic channel and are located on the same optical path. Eachsubstrate can contain one or more nanoparticle types immobilized ontothe same or distinct areas. In the example depicted in FIGS. 26B and26C, each substrate contains different nanoparticle types, one beingfunctionalized with a combination of specific capture molecules andblocking molecules, while the other with blocking molecules only.

The above components described for a transmission based measurementapparatus can also apply for reflection based measurement apparatus,with the exception that the light source and the detector are located onthe same side of the sample for a reflectance measurement.

Multiplexed designs of the self-referencing sensor systems mentionedherein are also possible. For example, in a multiplex design severalindependent sensors may be interfaced with one or several fluidicmicrochannels, or several fluidic channels may pass over different areason the same sensor containing nanoparticles. Multiplexed measurementscan be taken with multiple light sources and/or detectors.

To obtain two or more LSPR peaks, either a single nanoparticle type canbe used or a combination of multiple nanoparticle types. Thecomposition, size and shape of the nanoparticle type, effects theposition and intensity of the LSPR absorbance peak(s). As such, thenanoparticle type, or combination of nanoparticle types, should beselected such that the LSPR peaks do not overlap to a degree that wouldprohibit distinction of the peaks. In one embodiment at least twodistinct LSPR peaks having similar intensities, narrowfull-width-half-maxima and minimal (or no) spectral overlap, areselected.

Referring now to FIG. 27 , an example absorbance spectrum of a singlenanoparticle type immobilized onto a glass substrate is shown. Thisnanoparticle type produces two LSPR peaks due to the longitudinal andtransverse resonant modes of the rod particle shape. The two peaks aredistinct and can be individually tracked, therefore can be used for thesensor system.

In FIG. 28A, a photograph of the sensor containing two nanoparticletypes immobilized onto the same area of the glass substrate is shown.The resulting absorbance spectrum of the sensor is shown in FIG. 28B.The absorbance spectrum contains two distinct LSPR peaks, each of whichis contributed from the different particle types. The two peaks aredistinct and can be individually tracked and therefore can be used in aself-referencing sensor system.

The LSPR responses of the nanoparticles can be tracked by measuring theLSPR peak positions, peak intensities, the peak full-width-half-maximum(FWHM), peak shape, and/or any other property of the nanoparticles thatare sensitive to the surrounding environment. A single measurement type,or a combination of any thereof can be used.

In FIG. 29 , a diagram outlining an example sensor response is provided.This example sensor system uses two nanoparticle types to produce thetwo distinct LSPR peaks as seen in the absorbance spectra. Thenanoparticle type producing the LSPR peak at the shorter wavelength isfunctionalized with the specific capture molecule (the functionalizedparticles), whereas the second nanoparticle type producing the higherwavelength LSPR peak is functionalized with blocking molecules (theblocked particles). The LSPR response is being tracked by measuring thechange in the LSPR peak positions. In the scenario where the sensor isdetecting nonspecific effects only (top graph), a change in LSPR peakposition is observed with both peaks as they are both susceptible tothese events. In the scenario where the sensor is detecting specificbinding effects only (middle graph), a change in LSPR peak position isonly observed with the functionalized particles. If both specificbinding effects and nonspecific effects are present simultaneously(bottom graph), both LSPR peak positions will change; the functionalizedparticles will see both the specific and nonspecific binding events,whereas the blocked particles will only see the nonspecific bindingevents.

In one embodiment the self-referencing sensor may comprise ananoparticle type functionalized with only blocking molecules used incombination with another nanoparticle type being functionalized withcapture molecules. Using a self-referencing sensor of this type, it ispossible to correct the specific binding signal to remove anycontributing nonspecific effects. This is realized by subtracting thesignal sensed by the blocked nanoparticle from the signal sensed fromthe nanoparticle functionalized with capture molecules. A calibration ofthe signals may have to be performed prior to signal correction toaccount for any differences in the sensitivities or other propertiesthat may differ between the nanoparticle types.

In another embodiment, the self-referencing sensor includes the use ofone or more nanoparticle types producing at least two distinct LSPRpeaks, with all particle types being functionalized with the samecapture molecules. In one example two or more different nanoparticletypes functionalized with the same capture molecules may be used. Inthis case both particles will sense both the specific binding andnonspecific binding effects. The contributions of the specific bindingand nonspecific binding effects on the sensor signal can then beseparated using the LSPR sensing characteristic equations of eachnanoparticle type. In another example the self-referencing sensorcomprises a single nanoparticle type which produces at least twodistinct LSPR peaks. Since each LSPR peak usually corresponds todifferent dimensions of the nanoparticle, each LSPR peak has its owncharacteristic equation, which together can be used to separate thespecific binding and bulk effects.

Although examples are provided with reference to LSPR detectiontechniques, the above may also be adapted to other spectrometricdetection assays, for example, ELISA.

EXAMPLES Example 1 Comparison of 2D Design to T3D Design

An example of the improvements offered by the T3D design versus thetraditional 2D design is shown by comparison of FIG. 20 and FIG. 21 .FIG. 20 shows serial additions of the protein streptavidin into an AAOmembrane with 150 nm pores and 50 μm thick. Nanoparticles areimmobilized in the pores and have an LSPR peak around 627 nm. Thenanoparticles are functionalized with a biotin capture layer, withbiotin being chemically bound to the nanoparticles via a thiol bond. Thenon-specific sites are blocked with PEG. The sensor shows a response at0.5 nM streptavidin up to 20 nM in this case. 200 μL of streptavidin isintroduced at 20 μL/min. The detection limit is approximately 0.5nM forthis system. Serial additions of streptavidin are made over a glasssubstrate with the same nanoparticles immobilized on the surface of theglass. Biotin is attached to the surface of the nanoparticles using thesame chemistry as the T3D sensor. Streptavidin is injected serially at20 μL/min in volumes of 200 μL. The sensor shows a response at 5.0 nM upto 80 nM in this case. The detection limit is approximately 5.0 nM. Thisdemonstrates that the T3D sensor exhibits a 10× improvement in detectionlimit over the traditional 2D sensor, in this example case.

Example 2 Test Protocol for Fibronectin LSPR Sensor Testing PreparationSteps Buffer Preparation (“Tris”)

Buffer: 20 mM Tris, 100 mM NaCl, 0.005% Tween20, in nuclease free water,pH 7.4

-   -   1. Autoclave glassware and pipette tips (200 μL and 1000 μL) to        ensure nuclease free conditions.    -   2. For a 500 mL mixture weigh: 1.21 g Tris, 2.92 g NaCl and        0.025 g Tween 20 dissolve into 500 mL of dH₂O then measure the        pH of the solution. Adjust the pH up or down to 7.4 using a NaOH        or HCl solution.    -   3. Store in a sealed container at 4° C.

Fibronectin Protein Preparation

Stock: 0.5 mg/ml already dissolved in buffer

-   -   1. Aliquot into 54 μL volumes at 0.5 mg/ml in Tris Buffer        (Aliquot concentration=1.14 μM)    -   2. Stored in −20° C. Freezer

BSA Preparation

-   -   1. Take 10.5 mg BSA, add to 2 ml vial, add 1 ml Tris buffer.        This gives a 1% BSA solution. For a 0.1% solution add 70 uL of        1% BSA to 630 uL Tris buffer.    -   2. Store in a sealed container at 4° C.

Fibronectin Aptamer Preparation

Stock: 0.2 umol lypholized aptamer powder

-   -   1. Add 2 ml of Tris buffer to dry aptamer (makes 0.1 mM stock        concentration).    -   2. Aliquot into 50 uL vials at 0.1 mM.    -   3. Stored at −20° C.

Functionalization and Testing Procedure

-   -   1. Thaw one aptamer aliquot to room temperature. Add 430 μL of        Tris buffer to the aptamer aliquot to obtain a final        concentration of 10 μM (once the 20 μL of TCEP is added in the        next step). Vortex for 30 seconds to mix.    -   2. Make 2 ml of 40 mM stock TCEP by adding 20 mg TCEP to 2 ml of        Tris buffer and mixing well. From this stock add 20 μL to the        aptamer vial to give a final volume of 500 μL. Vortex for 30.        Leave at room temperature for 2 hours.    -   3. Fill up a 20 ml beaker with water and place on the hot plate        set at 90° C. Place the aptamer vial into the water bath for 3.5        minutes. Allow the aptamer to cool to room temperature.    -   4. Connect the T3D sensor and flow cell to the flow injection        analysis system which consists of a 6 port injection valve,        sample loop, and syringe pump. Set the pump speed to pump Tris        buffer at 0.01 ml/min. Load 500 μL of aptamer solution into a 1        mL syringe ensuring no bubbles are present. Load the aptamer        into a 500 μL sample loop and inject the solution via the        injection valve. The interaction time between the gold        nanoparticles and the aptamer will be approximately 50 minutes.    -   5. Once the solution has been fully pumped through the flow        cell, pump fresh Tris buffer through the system for 30 minutes.    -   6. Turn the injection valve back to “load”, and rinse out the        sample loop using Tris buffer. Use a 1 ml syringe and load 500        μL of 0.1% BSA into the sample loop. Inject at a pumping speed        of 0.01 ml/min.    -   7. Once the solution has been fully pumped through the flow cell        (after 50 minutes hour), pump fresh buffer through the system        for 30 minutes.    -   8. Disconnect the flow cell from the flow injection analysis        system and remove the T3D sensor. Dry the sensor gently with        nitrogen gas. If storing, store in a sealed container back        filled with nitrogen.    -   9. Load the dry T3D sensor into the testing flow cell. Insert        the flow cell into the reader unit and fill the cell with Tris        buffer. Begin acquiring optical transmission spectra and begin        tracking the LSPR peak position using the software. Acquire a        baseline peak position in Tris buffer.    -   10. Add 550 μL of Tris buffer to a Fibronectin protein aliquot.        This gives a Fibronectin concentration of 0.1 μM. Use a 1 ml        syringe and load 200 μL of the Fibronectin sample into the inlet        port of the flow cell. Activate the pump at 0.01 ml/min. The        protein sample will pump through the membrane interact with the        aptamer functionalized surface for 20 minutes.    -   11. Once the solution has been fully pumped through, acquire        another peak baseline in Tris. Find the difference between the        peak baseline from before and after the test. Using this value        and the standard curve of concentration vs. peak shift, find the        experimentally determine concentration of Fibronectin in the        sample.    -   12. Dispose of the sensor and flow cell.

Example 3 Test Protocol for Streptavidin LSPR Sensor TestingFunctionalization and Testing Procedure

Pump 10 mM 11-MUA (11-mercaptoundecanoic acid) and 1-OT (1-octanethiol)mixture (in a 3:1 ratio) in ethanol through the flow cell for 60 minutesat 0.01 ml/min.

Pump 13 mM PBS (phosphate buffered saline) through the flow cell for 30minutes at 0.1 ml/min.

Pump a 5 mM EDC/NHS solution through the flow cell for 60 minutes at0.01 ml/min.

Rinse with PBS for 30 minutes at 0.1 ml/min.

Pump 1 mM of Amine-PEG3-Biotin in 13 mM PBS at pH 6.5 at 0.01 ml/min for50 minutes. (PEG—polyethylene glycol)

Rinse with 13 mM PBS at 0.1 ml/min for 30 minutes.

Pump 500 μL of 25 μM low molecular weight PEG at 0.01 ml/min.

Pump 13 mM PBS through the flow cell for 30 minutes at 0.1 ml/min.

Disconnect the flow cell from the flow injection analysis system andremove the T3D sensor. Dry the sensor gently with nitrogen gas. Ifstoring, store in a sealed container back filled with nitrogen.

Load the dry T3D sensor into the testing flow cell. Insert the flow cellinto the reader unit and fill the cell with PBS buffer. Begin acquiringoptical transmission spectra and begin tracking the LSPR peak positionusing the software. Acquire a baseline peak position in buffer.

Load 200 μL of the streptavidin sample at 10 nM in PBS into the inletport of the flow cell. Activate the pump at 0.01 ml/min. The proteinsample will pump through the membrane interact with the functionalizedsurface for 20 minutes.

Once the solution has been fully pumped through, acquire another peakbaseline in buffer. Find the difference between the peak baseline frombefore and after the test. Using this value and the standard curve ofconcentration vs. peak shift, find the experimentally determineconcentration of streptavidin in the sample.

Dispose of the sensor and flow cell.

Example 4 Immobilization of Gold Nanoparticles into AAO Membrane PoresProcedure

Take AAO membrane from storage, inspect for cracks, chips or weak points

Rinse AAO membrane with deionized H₂O (dH₂O)

Load AAO membrane into flow cell and attach syringe connected to syringepump

Pump 3 mL of dH₂O through the membrane at 0.1 mL/min

Pump 2 mL of 2 μM poly-(succinyl-sulphonate)/0.4 μM CaCl₂ solution at pH3.1 through the membrane at 0.1 mL/min

Pump 6 mL of dH₂O through the membrane at 0.1 mL/min

Pump 2 mL of 2 μM polyallylamine hydrochloride/0.4 μM CaCl₂ solution atpH 3.1 through the membrane at 0.1 mL/min

Pump 6 mL of dH₂O through the membrane at 0.1 mL/min

Remove membrane from flow cell, examine for cracks and rinse surfacewith dH₂O

Pipette 0.01% w/v bovine serum albumin solution onto the surface of theAAO membrane, leave for 1 minute then rinse with dH₂O

Load AAO membrane into flow cell in reverse orientation as previous andattach syringe connected to syringe pump

Pump 3 mL of dH₂O through the membrane at 0.1 mL/min

Pump 10 mL of 0.1 nM gold nanoparticle mixture through the membrane at0.05 mL/min

Pump 6 mL of dH₂O through the membrane at 0.1 mL/min

If imaging: remove membrane from the flow cell, rinse with dH₂O

If testing: keep in flow cell and proceed to capture probefunctionalization steps. Connect flow cell to flow injection analysissystem.

Although examples are provided with reference to LSPR detectiontechniques, the above may also be adapted to other spectrometricdetection assays, for example, ELISA.

Example 5 Self-referencing Sensor Two-Nanoparticle System, One ParticleFunctionalized with Capture Molecule, the Other with Blocking Molecule(Streptavidin Detection)

FIG. 30 presents experimental data taken from a self-referencing sensorapparatus as described herein, using a sensor comprising two differenttypes of nanoparticles immobilized onto a glass substrate. The twonanoparticle types included gold spheres with a diameter of 40 nm andgold NanoUrchins with a diameter of 90 nm, with optical properties ofLSPR peak wavelengths around 530 nm and 630 nm respectively. Bothnanoparticle types were immobilized onto the same area of the glasssubstrate as shown in FIG. 28A, and produced two LSPR peaks at 536 nmand 635 nm as shown in FIG. 28B. The LSPR peaks were distinct with somespectral overlap, and could be individually tracked to monitor the LSPRsensing properties of each particle type. The 90 nm NanoUrchins werefunctionalized with a thiol-containing Biotin capture molecule(functionalized particle) to act as the specific sensing particle. The40 nm spheres were functionalized with a dithiolalkanearomatic-PEG3-OHblocking molecule (blocked particle). The experiment was carried outusing an LSPR apparatus in transmission mode similar to that describedin FIG. 25 . As a running buffer, 1× phosphate buffered saline (PBS) atpH 7.4 with 0.05% Tween20 and 0.1% BSA was used. Streptavidin at aconcentration of 3 nM diluted in running buffer was used as the analyte,and 1.5% glycerol (w/w) in running buffer was used to producenonspecific bulk refractive index shifts. To measure the LSPR sensingresponse of the nanoparticles, both peak positions were simultaneouslymeasured and recorded over time. First, the glycerol solution wasexposed to the surface for approximately 100 seconds, followed byintroduction of the same glycerol solution containing streptavidin forthe same amount of time. Upon the introduction of just the glycerolsolution (bulk only), a similar shape of response is seen for bothnanoparticle types. When exposed to the streptavidin-glycerol solution(streptavidin+bulk), the response of the functionalized particle showeda permanent peak shift indicating streptavidin binding with an apparentdistortion of the binding curve due to the glycerol bulk. The responseof the blocked particle however remained the same for that of the bulkonly, thus providing a reference signal for the nonspecific component ofthe glycerol-streptavidin mixture.

FIG. 31 contains the experimental raw and corrected biotin-streptavidinbinding curves from the data presented in FIG. 30 . The initial curve(black-solid) contains an obvious bulk distortion compared to thebulk-free reference curve shape (grey). The signal from the blockedparticle was used as the reference as it measured only the nonspecificeffects. As the sensitivities of both particle types used weredifferent, the reference signal was calibrated to that of the detectionsignal by normalizing the sensitivity of the blocked particle to that ofthe functionalized particle. Using the calibrated reference signalprovided by the blocked nanoparticle, the bulk effects were able to besubtracted and effectively removed from the distorted signal(black-dashed), resulting in a binding curve similar to that of thereference.

Example 6 Self-referencing Sensor Two-nanoparticle System, One ParticleFunctionalized with Capture Molecule, the Other with Blocking Molecule(His-tagged Molecule Detection)

FIG. 34 presents another example of experimental data obtained from aself-referencing sensor comprising two different types of nanoparticlesimmobilized onto a glass substrate. The two nanoparticle types includedgold spheres with a diameter of 40 nm and gold NanoUrchins with adiameter of 90 nm, with optical properties of LSPR peak wavelengthsaround 530 nm and 630 nm respectively. Both nanoparticle types wereimmobilized onto the same area of the glass substrate, and produced twoLSPR peaks at 535 nm and 638 nm as shown in FIG. 34A. The LSPR peakswere distinct with some spectral overlap, and could be individuallytracked to monitor the LSPR sensing properties of each particle type.The 90 nm NanoUrchins were functionalized with a thiol-containing NTAcapture molecule (functionalized particle) to act as the specificsensing particle. The 40 nm spheres were functionalized with adithiolalkanearomatic-PEG3-OH blocking molecule (blocked particle). Theexperiment was carried out using an LSPR apparatus in transmission modesimilar to that described in FIG. 25 . As a running buffer, 1× HEPESbuffered saline (HBS) at pH 7.4 with 0.005% Tween20 and 0.1% BSA wasused. Polyhistidine tagged (His6) streptavidin was used as the analyteat a concentration of 1000 nM containing 3.5% glycerol to produce anon-specific bulk signal in addition to specific binding. TheHis6-streptavidin with glycerol underwent serial dilution with runningbuffer to produce additional concentrations at 500 nM, 250 nM, 125 nMand 62.5 nM. To measure the LSPR sensing response of the nanoparticles,both peak positions were simultaneously measured and recorded over time.First, the surface was primed with several exposures of imidazole (200mM) and NiCl₂ (40 mM) for approximately 100 s each, before being exposedto solutions of glycerol (bulk) and 1000 nM His6-streptavidin+3.5%glycerol (Analyte+bulk) for the same amount of time. At least 600 safter the analyte+bulk exposure, imidazole was used 2-3 times toregenerate the NTA surface chemistry on the functionalized particle,followed by NiCl₂ exposure and glycerol solutions prior to the nextlower concentration of analyte+bulk. This process was repeated for allanalyte concentrations. The full sensor response of the functionalizedparticle and blocked particle is given in FIG. 34B. Upon analyte+bulkexposure, a prolonged shift in the LSPR peak position is observed withthe functionalized particle whereas only a short temporary shift isobserved with the blocked particle indicating that the blocked particleis not detecting specific binding but only the bulk shifts.

FIG. 35 contains the experimental raw and correctedNTA-His6-streptavidin binding curves from the data presented in FIG. 34. FIG. 35A presents the raw signals obtained from the functionalizedparticles and the blocked particles upon analyte exposure. The bindingcurves from the functionalized particle contains an obvious bulkdistortion (top graph), whereas no binding curves are seen with theblocked particle, as it only detected bulk effects acting as thereference signal (bottom graph). As the sensitivities of both particletypes used were different, the reference signal was calibrated to thatof the detection signal by normalizing the sensitivity of the blockedparticle to that of the functionalized particle. To reduce the noise ofthe reference signal, a moving average with n=21 was implemented. Usingthe calibrated reference signal provided by the blocked nanoparticle,the bulk effects were able to be subtracted and effectively removed fromthe distorted signal. The corrected binding responses are shown in FIG.35B.

Example 7 Self-referencing Sensor Two-nanoparticle System, One ParticleFunctionalized with Capture Molecule, the Other with Blocking Molecule(Streptavidin Detection with Different Nanoparticle Combination)

FIG. 36 presents experimental data taken from a self-referencing sensorapparatus as described herein, using a sensor comprising a differentcombination of two nanoparticle types immobilized onto a glasssubstrate. The two nanoparticle types included gold spheres with adiameter of 80 nm and gold NanoUrchins with a diameter of 100 nm, withoptical properties of LSPR peak wavelengths around 550 nm and 648 nm insolution respectively. Both nanoparticle types were immobilized onto thesame area of the glass substrate as shown in FIG. 36A, and produced twoLSPR peaks at 543 nm and 650 nm after functionalization as shown in FIG.36B. The LSPR peaks were distinct and could be individually tracked tomonitor the LSPR sensing properties of each particle type. The 100 nmNanoUrchins were functionalized with a thiol-containing Biotin capturemolecule (functionalized particle) to act as the specific sensingparticle. The 80 nm spheres were functionalized with adithiolalkanearomatic-PEG3-OH blocking molecule (blocked particle). Theexperiment was carried out using an LSPR apparatus in transmission modesimilar to that described in FIG. 25 . As a running buffer, 1× phosphatebuffered saline (PBS) at pH 7.4 with 0.05% Tween20 was used at aconstant flow rate of 75 μL/min. Streptavidin diluted in running bufferwas used as the analyte, and 25 mg/mL of sugar dissolved in distilledwater was used to produce nonspecific bulk refractive index shifts. Tomeasure the LSPR sensing response of the nanoparticles, both peakpositions were simultaneously measured and recorded over time. First,streptavidin at a concentration of 11.1 nM was exposed to the surfacefor approximately 100 seconds, followed by introduction of 33.3 nMStreptavidin, then 25 mg/mL sugar to produce a bulk refractive indexchange for the same amount of time. FIG. 36C shows the responses of bothnanoparticle types. Upon the introduction of just the sugar solution(bulk), a similar temporary signal change is seen for both nanoparticletypes. When exposed to the streptavidin solutions, the response of thefunctionalized particle showed a permanent peak shift indicatingstreptavidin binding and detection. For the blocked particle, noresponse was observed upon introduction of streptavidin, indicating nobinding or specific detection from this particle type. Therefore theblocked particle was able to provide a reference signal for only thenon-specific interactions.

Example 8 Self-referencing Sensor, Two-Nanoparticle System, BothParticles Functionalized with the Same Capture Molecule

FIG. 32 presents experimental data taken from a self-referencing sensorapparatus composed of two nanoparticle types immobilized onto a glasssubstrate, both having the same functional surface. The two nanoparticletypes included gold spheres with a diameter of 40 nm (particle 2) andgold NanoUrchins with a diameter of 90 nm (particle 1), with opticalproperties of LSPR peak wavelengths around 530 nm and 630 nmrespectively. Both nanoparticle types were immobilized onto the samearea of the glass substrate similar to that shown in FIG. 28A, andproduced two LSPR peaks at 534 nm (particle 2) and 618 nm (particle 1)similar to that shown in FIG. 28B. The LSPR peaks were distinct withsome spectral overlap, and could be individually tracked to monitor theLSPR sensing properties of each particle type. In this example,HS-PEG_(2k)-MeOH was used as the analyte at a concentration of 0.333 mM(a). As the thiol portion of the analyte binds directly to gold, bothnanoparticle types were left as bare gold surfaces in place ofadditional functionalization with a capture molecule. To produce bulkrefractive index shifts (b), solutions containing 8%, 15% or 22%glycerol (w/w in water) were used. The experiment was carried out usingan LSPR apparatus in transmission mode similar to that described in FIG.25 and water was used as the running buffer. To measure the LSPR sensingresponse of the nanoparticles, both peak positions were simultaneouslymeasured and recorded over time. First, three glycerol solutions (8%,15%, 22% respectively) were exposed to the surface for approximately 100seconds (b), followed by introduction of the analyte (a), and a finalinjection of 8% glycerol for the same period of time. As seen in FIG.32A, introduction of the glycerol solutions (a) produced temporarysensor responses while the analyte (b) produced a permanent bindingshift of both LSPR signals. It is clear that the responses of eachparticle type are different. Using the characteristic equations of bothnanoparticle types, the binding signal was able to be separated from thebulk signals. The resulting separated binding and bulk signals forparticle 1 are shown in FIG. 32B.

Example 9 Self Referencing Sensor, Single-nanoparticle System

FIG. 33 contains experimental data taken from a self-referencing sensorcomposed of a single nanoparticle type. In this example, gold nanorodshaving dimensions of 40 nm×80 nm were used, with longitudinal andtransverse LSPR peaks at 660 nm and 527 nm respectively. Whenimmobilized onto a glass substrate, both the transverse and longitudinalsignals produced two distinct LSPR peaks at 537 nm and 677 nmrespectively, as shown in FIG. 27 . The nanorods were functionalizedwith a thiol-containing biotin capture molecule. The experiment wascarried out with a transmission-based self-referencing sensor apparatusdescribed in FIG. 25 . As a running buffer, 1× PBS at pH 7.4 with 0.05%Tween20 was used. Streptavidin at a concentration of 1 μM diluted inrunning buffer was used as the analyte, and 8% glycerol (w/w) was usedto produce bulk refractive index shifts. To measure the LSPR sensingresponse of the nanoparticles, both peak positions were simultaneouslymeasured and recorded over time. All solutions were exposed to thesensor surface for approximately 150 seconds. As shown in FIG. 33A,introduction of the glycerol solution (a) produced temporary sensorresponses while the specific sensing molecule (b) produced a permanentbinding shift of both LSPR peak positions. Both peaks showed differentsensing responses. Using the characteristic equations governing thesensing abilities of both LSPR peaks, the binding signal was able to bedistinguished from the bulk signals. The resulting separated signals assensed from the longitudinal LSPR peak are shown in FIG. 33B.

Example 10 Solution-phase Self-referencing Sensor, Two-nanoparticleSystem

FIG. 37 presents experimental data taken from a self-referencing sensorapparatus as described herein, using a solution-phase sensor comprisingtwo nanoparticle types. The two nanoparticle types included gold sphereswith a diameter of 40 nm and gold NanoUrchins with a diameter of 80 nm.The 40 nm spheres were functionalized with a methoxy-PEG5000-SH blockingmolecule (blocked particle) and the 80 nm NanoUrchins werefunctionalized with streptavidin as a capture molecule (functionalizedparticle) with LSPR peak wavelengths around 530 nm and 620 nm,respectively. Both nanoparticle types were mixed in a solution of 0.01×PBS and placed into a semi-micro polystyrene cuvette as shown in FIG.37A, and produced two LSPR peaks at 532 nm and 612 nm as shown in FIG.37B. The LSPR peaks were distinct and could be individually tracked tomonitor the LSPR sensing properties of each particle type. Theexperiment was carried out using an LSPR apparatus in transmission mode.Biotinylated anti-rabbit IgG (stock concentration 3 mg/mL) was used asthe analyte, and a glycerol solution was used to produce nonspecificbulk refractive index shifts. To measure the LSPR sensing response ofthe nanoparticles, both peak positions were simultaneously measured andrecorded over time. The response of both nanoparticles over time isshown in FIG. 37C. The anti-rabbit IgG was added to the sensor solution2 μg at a time (a), with at least 10 minutes between additions. Afterthe third addition of anti-rabbit IgG, 60% glycerol (w/w in H2O) wasadded to the sensor solution to produce a final concentration of 3%glycerol, creating a bulk refractive index shift (b). Immediately aftereach addition, the sensor solution was mixed by pipetting, causing briefinterruption of the signal and producing large spikes on the responsegraphs, which can be ignored. Upon the introduction of the glycerolsolution, a similar immediate signal change is seen for bothnanoparticle types as it produced a non-specific bulk refractive indexchange. With addition of the anti-rabbit IgG, the response of thefunctionalized particle showed a peak shift indicating binding anddetection. The peak shifted gradually over time due to effect ofdiffusion of the analyte, producing final LSPR peak shifts ofapproximately 500 pm. For the blocked particle, no response was observedupon introduction of anti-rabbit IgG, indicating no binding or specificdetection from this particle type. Therefore the blocked particle wasable to provide a reference signal for only the non-specificinteractions.

Although the above has been described with reference to certain specificexample embodiments, various modifications thereof will be apparent tothose skilled in the art without departing from the scope of the claimsappended hereto.

1.-19. (canceled)
 20. An LSPR apparatus comprising: at least oneself-referencing sensor for detection of a target chemical andsimultaneous detection of non-specific signals, the at least oneself-referencing sensor comprising one or more nanoparticles, whereinthe one or more nanoparticles are configured to simultaneously emit aLSPR target chemical signal and at LSPR reference signal, wherein atleast one nanoparticle of the one or more nanoparticles isfunctionalized with one or more capture molecules to bind the targetchemical resulting in the LSPR target chemical signal; wherein each ofthe one or more nanoparticles comprises a decay length corresponding toa size of a capture-target complex comprising the one or more capturemolecules and the target chemical; and a light source configured toproject light through the at least one self-referencing sensor and ontoa detector.
 21. The LSPR apparatus of claim 20, wherein the one or morenanoparticles comprises two or more nanoparticle having distinct LSPRpeaks.
 22. The LSPR apparatus of claim 20, wherein the one or morenanoparticles comprises a shape selected from the group comprising rods,stars, urchins, decahedra, hexagons, triangles, shells, prisms,platelets, spheres, rice, plates, cubes, cages, stars, bipyramids, or acombination thereof.
 23. The LSPR apparatus of claim 20, wherein the oneor more nanoparticles comprises gold, silver, platinum, gold coatedsilver, silver coated gold, or any combination thereof.
 24. The LSPRapparatus of claim 20, wherein the one or more nanoparticles isfunctionalized with the same one or more capture molecules.
 25. The LSPRapparatus of claim 20, wherein the LSPR reference signal corresponds tonon-specific signals.
 26. The LSPR apparatus of claim 20, wherein theone or more nanoparticles has a size ranging from about 1 nm to about1000 nm in at least one dimension.
 27. The LSPR apparatus of claim 20,wherein at least one of the one or more nanoparticles is functionalizedwith a blocking molecule which blocks binding of the target chemical.28. The LSPR apparatus of claim 20, wherein the one or morenanoparticles comprises three or more nanoparticles, wherein at leastone of the three or more nanoparticles is functionalized with a blockingmolecule and wherein each of the remaining three or more nanoparticlesis functionalized with a different capture molecule.
 29. The LSPRapparatus of claim 20, wherein the one or more capture moleculescomprise an aptamer, antibody, nucleic acid, protein, small molecule orpolymer.
 30. The LSPR apparatus of claim 20, wherein the one or morenanoparticles of the at least one self-referencing sensor is immobilizedonto the at least one self-referencing sensor.
 31. A chemical sensingsystem comprising: a fluidic cartridge comprising an inlet and at leastone sensor for LSPR detection of a target analyte located between thelight source and the detector, the at least one sensor comprising amembrane, the membrane comprising pores and a plurality of nanoparticlesimmobilized on a surface of the pores, wherein the plurality ofnanoparticles being functionalized with one or more capture moleculesand wherein each of the plurality of nanoparticles comprises a decaylength corresponding to a capture-target complex comprising the one ormore capture molecules and the target analyte, wherein the membrane issubstantially transparent and substantially porous; and a light sourcefor LSPR measurement, the light source arranged to emit onto a detector;a signal processor in electronic communication with the light source andthe detector.
 32. The chemical sensing system of claim 31, wherein thechemical sensing system is configured to detect the presence of at leastone target analyte.
 33. The chemical sensing system of claim 31, whereinthe detector is configured simultaneously detect a first LSPR targetanalyte signal and a LSPR reference signal in response to light from thelight source interacting with the at least one sensor.
 34. The chemicalsensing system of claim 33, wherein the at least one sensor issubstantially transparent and is disposed between the light source andthe detector such that the first LSPR target analyte signal and the LSPRreference signal are detected in transmission mode.
 35. A method ofdetecting the presence of an analyte, the method comprising: contactinga sample with a plurality of sensors, wherein the sample comprises atleast one chemical target; wherein the plurality of sensors comprises amembrane, the membrane comprising a plurality of nanoparticles, each ofthe plurality of nanoparticles comprising at least one capture moleculeand comprises a decay length corresponding to a complex comprising theat least one capture molecule and the at least one chemical target; andbinding the at least one chemical target to the plurality of sensors,wherein each of the plurality of sensors generates a LSPR target signalcorresponding to the complex; and measuring the LSPR target signalgenerated by the complex and a LSPR reference signal.
 36. The method ofclaim 35, wherein the membrane comprises a nanoporous material, thenanoporous material comprising a plurality of pores.
 37. The method ofclaim 36, wherein one of the plurality of nanoparticles comprises acapture molecule functionalized with a blocking molecule.
 38. The methodof claim 37, wherein the LSPR reference signal corresponds to thecapture molecule functionalized with a blocking molecule.
 39. The methodof claim 36, wherein the plurality of sensors is located on an inside ofthe plurality of pores of the nanoporous material.